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This is the published version of a paper published in Applied and Environmental Microbiology.
Citation for the original published paper (version of record):
Gillman, A., Muradrasoli, S., Söderstrom, H., Holmberg, F., Latorre-Margalef, N. et al. (2015)
Oseltamivir-Resistant Influenza A (H1N1) Virus Strain with an H274Y Mutation in
Neuraminidase Persists without Drug Pressure in Infected Mallards.
Applied and Environmental Microbiology, 81(7): 2378-2383
http://dx.doi.org/10.1128/AEM.04034-14
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Oseltamivir-Resistant Influenza A (H1N1) Virus Strain with an H274Y
Mutation in Neuraminidase Persists without Drug Pressure in Infected
Mallards
Anna Gillman,a,b Shaman Muradrasoli,b,c Hanna Söderström,d Fredrik Holmberg,a Neus Latorre-Margalef,e* Conny Tolf,e
Jonas Waldenström,e Gunnar Gunnarsson,f Björn Olsen,a,b Josef D. Järhulta,b
Influenza A virus (IAV) has its natural reservoir in wild waterfowl, and emerging human IAVs often contain gene segments from
avian viruses. The active drug metabolite of oseltamivir (oseltamivir carboxylate [OC]), stockpiled as Tamiflu for influenza pandemic preparedness, is not removed by conventional sewage treatment and has been detected in river water. There, it may exert
evolutionary pressure on avian IAV in waterfowl, resulting in the development of resistant viral variants. A resistant avian IAV
can circulate among wild birds only if resistance does not restrict viral fitness and if the resistant virus can persist without continuous drug pressure. In this in vivo mallard (Anas platyrhynchos) study, we tested whether an OC-resistant avian IAV (H1N1)
strain with an H274Y mutation in the neuraminidase (NA-H274Y) could retain resistance while drug pressure was gradually
removed. Successively infected mallards were exposed to decreasing levels of OC, and fecal samples were analyzed for the neuraminidase sequence and phenotypic resistance. No reversion to wild-type virus was observed during the experiment, which included 17 days of viral transmission among 10 ducks exposed to OC concentrations below resistance induction levels. We conclude that resistance in avian IAV that is induced by exposure of the natural host to OC can persist in the absence of the drug.
Thus, there is a risk that human-pathogenic IAVs that evolve from IAVs circulating among wild birds may contain resistance
mutations. An oseltamivir-resistant pandemic IAV would pose a substantial public health threat. Therefore, our observations
underscore the need for prudent oseltamivir use, upgraded sewage treatment, and surveillance for resistant IAVs in wild birds.
I
nfluenza A virus (IAV) can infect many mammalian and avian
species, although wild waterfowl, primarily dabbling ducks, are
the principal reservoir host (1, 2). New human IAVs, including
pandemic viruses, may contain gene segments of avian origin (1,
3). IAV infection in waterfowl is mainly gastrointestinal and generates very limited symptoms (1, 4). In contrast to mammalian
IAVs, where relatively limited numbers of subtypes circulate,
avian viruses are genetically variable, with multiple subtype combinations cocirculating and with a high rate of genome reassortment (1, 5). At the interface between wild and domesticated waterfowl, poultry, swine, and humans, new IAV strains evolve. New
strains can emerge through reassortment of gene segments in
coinfected individuals and by subsequent point mutations under
immunologic or host-adaptive selective pressure (1, 3, 6).
There are limited means for responding to a severe influenza
pandemic, and currently, preparedness plans worldwide rely almost entirely on the neuraminidase inhibitor (NAI) oseltamivir
(Tamiflu) (7, 8). Viral resistance to anti-influenza drugs is well
known to emerge in humans under treatment. All currently circulating human H3N2 and H1N1 lineages are largely resistant to
adamantanes, which are no longer recommended for the treatment of seasonal influenza (9). Oseltamivir exerts its inhibitory
effect through the active metabolite oseltamivir carboxylate (OC)
by binding to the active enzymatic site of neuraminidase (NA).
Resistance to OC is caused primarily by mutations that change the
shape of the catalytic site, by changes in either active-site residues
or framework supportive residues. The two phylogenetic groups
of NAs (N1 and N2) differ slightly in sensitivity to the drug and
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have distinct resistance mutations; H274Y (N2 numbering) is
most common in N1, while R292K and E119V are most common
in N2 (10). Treatment of IAV-infected individuals with an NAI
can generate resistant viruses, as has been reported in infections
with both human (11) and avian H5N1 (12) and H7N9 (13)
strains. Of more concern, however, is the circulation of NAI-resistant human influenza A (H1N1) virus strains in the absence of
selective drug pressure, which has been reported primarily for the
seasonal influenza A (H1N1) 2008-2009 virus (14) and for clusters
of influenza A (H1N1)/pdm2009 viruses (15).
To date, surveillance of antiviral resistance in avian IAVs from
Received 11 December 2014 Accepted 16 January 2015
Accepted manuscript posted online 23 January 2015
Citation Gillman A, Muradrasoli S, Söderström H, Holmberg F, Latorre-Margalef N,
Tolf C, Waldenström J, Gunnarsson G, Olsen B, Järhult JD. 2015. Oseltamivirresistant influenza A (H1N1) virus strain with an H274Y mutation in neuraminidase
persists without drug pressure in infected mallards. Appl Environ Microbiol
81:2378 –2383. doi:10.1128/AEM.04034-14.
Editor: H. L. Drake
Address correspondence to Anna Gillman, [email protected].
* Present address: Neus Latorre-Margalef, Department of Population Health,
College of Veterinary Medicine, Southeastern Cooperative Wildlife Disease Study,
University of Georgia, Athens, Georgia, USA.
Copyright © 2015, American Society for Microbiology. All Rights Reserved.
doi:10.1128/AEM.04034-14
The authors have paid a fee to allow immediate free access to this article.
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April 2015 Volume 81 Number 7
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Section for Infectious Diseases, Department of Medical Sciences, Uppsala University, Uppsala, Swedena; Zoonosis Science Centre, Department of Medical Biochemistry
and Microbiology, Uppsala University, Uppsala, Swedenb; Department of Biomedical Sciences and Veterinary Public Health, Swedish University of Agricultural Sciences,
Uppsala, Swedenc; Department of Chemistry, Umeå University, Umeå, Swedend; Centre for Ecology and Evolution in Microbial Model Systems, Linnaeus University,
Kalmar, Swedene; Division of Natural Sciences, Kristianstad University, Kristianstad, Swedenf
Persistence of Oseltamivir-Resistant IAV in Mallards
MATERIALS AND METHODS
Virus. In our experiments, we used an avian H1N1 isolate with the H274Y
resistance mutation in NA, Influenza A/Mallard/Sweden/51833/2006
(H1N1)/NA-H274Y (referred to below as A/51833/H274Y). This isolate
originated from the wild-type (wt) Influenza A/Mallard/Sweden/51833/
2006 (H1N1) isolate (referred to below as A/51833/wt), which had been
recovered from a wild mallard in southern Sweden (4) (GenBank accession number of NA, AEA02276). The A/51833/wt isolate had previously
been isolated, subtyped, and experimentally exposed to OC in the same
mallard model as that used in these experiments, as described in reference
23. The experimentally evolved A/51833/H274Y virus (23) was propagated in specific-pathogen-free embryonated chicken eggs as described in
detail in reference 24 and was titrated based on the 50% embryo infective
dose (EID50) (26), to 108.4 EID50/ml allantoic fluid, which was used as the
viral stock solution.
Drugs. OC and deuterium-labeled OC were obtained from F. Hoffmann-La Roche Ltd., Basel, Switzerland. Zanamivir (ZA) was purchased
locally as Relenza (GlaxoSmithKline). The drugs were dissolved in MilliQ
water and were stored at ⫺20°C.
Mallard model. Male mallards, 2 to 3 months old, were purchased
from a Swedish game farm and were kept isolated indoors at the animal
facilities of the National Veterinary Institute of Sweden, after ethical approval by the Ethical Committee on Animal Experiments in Uppsala (permit C201/11) and in accordance with legislation and recommendations
from the Swedish Agricultural Board. Before the start of the experiment,
the ducks tested negative for present or previous IAV infection. Serological tests (Avian Influenza Virus Antibody test kit; IDEXX Laboratories
Europe, The Netherlands) were carried out on blood samples taken from
all ducks upon arrival at the facility, and fecal samples, collected on the day
of entry into the experiment, were tested by real-time reverse transcriptase
PCR (RRT-PCR) targeting the IAV matrix gene (see below).
At the start of the experiment, two mallard ducks (“generation 1”)
were infected by inoculation of 1 ml of the A/51833/H274Y viral stock
solution into the esophagus and were placed in an experimental room that
contained a single 170-liter water pool for swimming and drinking, as well
as feed ad libitum. Prior to the experiment, OC was added to the water to
a final concentration of 79 ␮g/liter (278 nM); thereafter, the water was
changed daily, and OC was added according to the intended concentra-
April 2015 Volume 81 Number 7
TABLE 1 Experimental model with decreasing OC exposure of IAVinfected mallards
OC concn in
water (␮g/liter)a
Day (SE)
0
1
2
3
4
5
6
7
8
9
10
11
12
13
14
15
16
17
18
19
20
21
22
23
24
25
26
27
28
29
30
31
32
Presence of the following generationb in the
experimental room:
G1 G2 G3 G4 G5 G6 G7 G8 G9 G10
79 (3.7)
30 (0.54)
11 (0.47)
2.5 (0.35)
0.93 (0.068)
0.26 (0.0045)
0.069 (0.0062)
0.027 (0.0018)
0.0083 (0.00059)
0
a
Mean concentration for three experimental days.
Shading indicates presence. G, generation. Each generation consisted of two mallard
ducks.
b
tions. Three days postinoculation (p.i.), the OC concentration was reduced to 30 ␮g/liter (106 nM); two uninfected ducks (generation 2) were
introduced and were housed in the experimental room together with generation 1 for 2 days, to allow viral transmission. At 5 days p.i., generation
1 was euthanized by intravenous injection of sodium pentobarbital (100
mg Pentobarbital vet. [100 mg/ml] per kg of body weight). At 6 days p.i.,
the OC concentration was reduced to 11 ␮g/liter (39 nM), and two new
mallards were introduced and were housed together with generation 2.
This procedure, with overlapping generations and decreasing OC concentrations, was repeated for 10 generations of ducks over 32 days (Table 1).
OC concentrations were successively reduced (to 2.5, 0.93, 0.26, 0.069,
0.027, and 0.0083 ␮g/liter) until 26 days p.i., after which no OC was added
to the water (days 27 to 32 p.i.) (Table 1).
Fecal samples from individual birds were collected daily by putting
each bird in a clean box for 5 to 20 min and then swabbing feces from the
box. On a few occasions, when birds did not defecate, samples were obtained by cloacal swabbing. Water samples for viral detection were taken
daily. Although the individual mallards were successively replaced, the
experiment was designed to allow continuous propagation and evolution
of the viral population under decreasing drug pressure. Naïve individuals
were introduced at peak viral shedding, after 2 days, to facilitate transmis-
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wild birds has been limited. There is, however, accumulating evidence that waterfowl can be exposed to NAIs in the environment,
which may cause selection of resistant IAV variants in the natural
reservoir. OC, the drug primarily studied, is inefficiently removed
by conventional sewage water treatment (16, 17). Consequently,
OC can be discharged to water environments where waterfowl
reside, and OC concentrations as high as 865 ng/liter have been
detected in surface water (18–20). If avian IAV is exposed to OC in
its natural host and acquires resistance, there is a risk that emerging human-pathogenic IAV strains carrying avian gene segments
may be resistant (21). NAI resistance in an emerging pandemic
virus would be a substantial public health concern, especially in
the early phase of a pandemic, before new, efficient vaccines could
be distributed (22).
In vivo experiments have demonstrated that OC resistance
evolves in avian IAVs of both the N1 and N2 neuraminidase
groups when infected mallards (Anas platyrhynchos) are exposed
to 0.95 to 12 ␮g/liter OC in their water (23–25). However, a fundamental question for the persistence of NAI resistance in the
environment is whether a resistance mutation is retained without
continuous selective drug pressure. To address this question, we
examined the persistence of OC resistance in an avian influenza A
(H1N1)/NA-H274Y virus strain during natural transmission and
replication in mallard ducks.
Gillman et al.
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FIG 1 Viral shedding in feces from mallards was quantified by RRT-PCR of
the IAV matrix gene. CT values of ⬎45 were considered to indicate a negative
sample. Whiskers indicate standard errors of the means for two samples. The
number of days after inoculation (for generation 1 [g1]) or after introduction
to the experimental room (for g2 to g10) is shown along the x axis. Each
generation consisted of two mallard ducks.
after OC addition during the periods of highest (79-␮g/liter) and lowest
(0.008-␮g/liter) OC exposure. An on-line solid-phase extraction–liquid
chromatography–tandem mass spectrometry (SPE–LC–MS-MS) system
was used to verify the OC concentrations during the experiment. The
SPE–LC–MS-MS system used was the same as that described in detail in
reference 23, except that an Oasis HLB extraction column (length, 20 mm;
inside diameter, 2.1 mm; particle size, 15 ␮m; Waters S.A.S., Saint-Quentin-en-Yvelines, France) was used here. Briefly, 10 ml of each water sample was filtered and acidified (0.1% formic acid by volume), and 1 ml was
then analyzed by the SPE–LC–MS-MS system (for the highest exposure
level, the samples were diluted 1/10 with water). Samples were quantified
by an internal standard method with deuterated OC as the internal standard and with six calibration points.
RESULTS
Quantification of OC in water. Table 1, presenting the mean OC
concentration (n ⫽ 3) and standard error (SE) at each exposure
level, shows that the daily OC concentration at each level was
relatively stable. The differences in the average OC concentration
between freshly prepared water and water tested after 24 h were
low (5% at 79 ␮g/liter and 8% at 0.008 ␮g/liter), showing that the
OC concentrations were stable over a 24-h exposure period. Thus,
the variation in OC concentrations within and between experimental days was low. The limit of quantification (LOQ) for the
SPE–LC–MS-MS method was 1 ng/liter, and the linearity (R2) of
the calibration curve was 1.0000.
Viral detection and NA genotype. All birds in the experiment
were successfully infected, as determined by IAV shedding in fecal
samples, which was detected from 2 days p.i. in generation 1 and
from the first day after introduction in all following generations
(Fig. 1). Virus was detected in experimental water from 2 days p.i.
all through the experiment, with a mean RRT-PCR cycle threshold
(CT) value of 31 (SE, 0.56).
Standard sequencing of 103 fecal samples from all generations
of the experiment showed that all contained the NA H274Y mutation, with no visible wild-type residue at position 274. At NA
amino acid residue 222, the A/51833/H274Y virus, like the original A/51833/wt virus, had asparagine (N), which differs from the
more common residue at this site, isoleucine (I).
The results of targeted deep sequencing of the codon for NA
amino acid 274 did not differ between early fecal samples, from 4
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sion. Between the euthanasia of one generation and the introduction of a
new one, there was a 1-day gap to ensure continuous virus transmission
between generations (e.g., generation 1 was removed 1 day before generation 3 was introduced, to make sure that generation 3 was infected by
virus from generation 2 and not from generation 1). OC exposure levels
ranging from approximately 80 ␮g/liter (a concentration at which the
mutant A/51833/H274Y virus was known to dominate completely [23])
to zero were chosen, and half of the concentrations were lower than the
resistance induction level of 0.95 ␮g/liter (23).
Viral detection and sequencing of neuraminidase. Viral RNA was
extracted from fecal samples, water isolates, and egg isolates in a Magnatrix 8000 extraction robot (Magnetic Biosolutions) with a Vet Viral NA kit
(NorDiag ASA). IAV was detected and quantified by RRT-PCR targeting
the IAV matrix gene (27) using an iScript one-step reverse transcriptase
PCR (RT-PCR) kit for probes (Bio-Rad); 25-␮l reaction mixtures were
run in a Rotor-Gene 2000 real-time thermocycler (Corbett Research) as
described in detail in reference 24.
NA was amplified from IAV-positive fecal samples by one-step RTPCR using primers designed previously for amplifying and sequencing the
NA of A/51833/wt (Thermo Hybaid, Interactiva Division) and a SuperScript III One-Step RT-PCR system with Platinum Taq High Fidelity
DNA polymerase (Life Technologies) as described in reference 23, with 1
␮l enzyme mixture and 400 nM each primer. PCR products were confirmed by gel electrophoresis and were purified by ExoSAP-IT treatment
(Affymetrix Inc.); 2 ␮l of the reagent was used to purify 24 ␮l of PCR
product. Amplicons were sequenced by Macrogen Inc. in South Korea or
The Netherlands using two forward primers (primers 1 and 5) and two
reverse primers (primers 2 and 6) as presented in Table 2 of reference 23.
The sequencing results were analyzed in SeqScape software, version 2.7
(Applied Biosystems), with the NA sequence of A/51833/wt as the reference.
To further evaluate the possible reemergence of wild-type virus at a
proportion too small to discover by standard Sanger sequencing, deep
sequencing was performed on three early (generations 1 and 2) and three
late (generation 10) fecal samples from the experiment. RNA was extracted with TRIzol (Life Technologies), reverse transcribed, and PCR
amplified using the PathAmp FluA Reagents with high-fidelity polymerase (revision B.0; Life Technologies). The resulting amplicons were purified using the Agencourt AMPure XP reagent (Beckman Coulter) and
were quantified, and libraries were prepared with the Ion Xpress Plus
fragment library kit (Life Technologies). After size selection on the
BluePippin instrument (Sage Science), samples were quantified using the
Fragment Analyzer instrument (Advanced Analytical Technologies) and
were pooled, followed by emulsion PCR on the Ion OneTouch 2 system
with Ion PGM Template OT2 400 kit (Life Technologies) chemistry. Enrichment was carried out using the Ion OneTouch enrichment system
(ES) (Life Technologies). Samples were loaded onto an Ion 316 chip and
were sequenced on the Ion PGM system using Ion PGM Sequencing 400
kit (read length, 400 bp; Life Technologies) chemistry.
Phenotypic resistance testing. To test NA inhibition by OC and ZA,
16 fecal samples (eight from generation 1 or 2 and eight from generation
10) were propagated in embryonated chicken eggs as described above. The
obtained isolates were subjected to standard Sanger sequencing (as described above for fecal samples) to confirm resistance after egg propagation. NA inhibition by OC and ZA was determined from duplicate
samples in 96-well plates using the fluorogenic substrate 2=-(4-methylumbelliferyl)-␣-D-N-acetylneuraminic acid (MUNANA; Sigma) (28) and
serial dilutions (0.015 to 4,000 nM) of OC and ZA; the fluorescent product
was detected in a GloMax-Multi microplate multimode reader (Promega)
as described in reference 23. Fifty percent inhibitory concentrations
(IC50) were calculated in GraphPad Prism software, version 5 (GraphPad).
OC concentration in water. Water samples were collected daily after
24 h of exposure (when the water was changed). To verify the stability of
the OC concentration over 24 h, water samples were also collected directly
Persistence of Oseltamivir-Resistant IAV in Mallards
TABLE 2 Targeted deep sequencing of the codon for NA amino acid
residue 274
Virus or sample
Time of
sampling
(days p.i.)
Viruses
A/51833 (H1N1)/wt
A/51833 (H1N1)/H274Y
4
6
6
30
30
31
A
C
G
T
Consensus
codon for
NA aa 274
0
3
550
4
0
1
3
742
CAC
TAC
2
2
5
4
3
1
2
1
3
1
0
1
0
0
3
1
3
0
283
202
423
654
863
606
TAC
TAC
TAC
TAC
TAC
TAC
a
Fecal samples from mallards, labeled by generation and mallard number (e.g., “g 2:1”
stands for mallard number 1 of generation 2).
and 6 days p.i., and late samples, from 30 and 31 days p.i. The CAC
codon codes for the wild-type amino acid histidine (H), and TAC
codes for tyrosine (Y); the latter dominated by more than 99% in
all samples from the experiment. The total numbers of reads at the
NA-274 site were 205 to 869 for experimental samples and viral
inoculants. Both early and late experimental samples had ⬍1%
nonthymine (non-T) nucleotide reads and no more cytosine (C)
reads than the sequencing noise of adenine (A) and guanine (G)
combined (Table 2).
Phenotypic resistance results. The mean IC50 of OC for the 16
duplicate samples tested was 549 nM (SE, 38.5 nM), with no significant difference between early and late samples (P ⫽ 0.081; 95%
confidence interval [95% CI] for differences in means, ⫺18.9 to
286 nM, with a two-sided t test for independent samples) (Fig. 2).
There was no reduction in sensitivity to ZA (IC50, 0.31 nM [SE,
0.038 nM]). For the original A/51833/wt virus, the mean IC50 of
OC from 6 repeated assays was 1.6 nM (SE, 0.22 nM), and that of
ZA was 0.43 nM (SE, 0.099 nM) (Fig. 2).
DISCUSSION
In order for a resistant avian IAV to retain its resistance trait when
exposed to little or no drug, and hence to circulate in a wild bird
population, the virus has to harbor the resistance mutation(s)
with no loss of viral fitness. In this in vivo study, when we gradually
decreased the level of OC exposure for mallards infected with an
OC-resistant avian influenza A (H1N1)/NA-H274Y virus, and finally removed OC altogether, we found no genotypic or phenotypic decrease in resistance and no reversion to wild-type virus.
Targeted deep sequencing of the resistance point mutation did not
indicate any tendency for the wild-type virus to reemerge when
the drug pressure was below the level of induction of the NAH274Y mutation (0.95 ␮g/liter [23]) or when OC had been removed. Based on the number of reads and the fact that the wildtype genotype was never more prevalent than the sequencing
noise, we can rule out a wild-type subpopulation with a prevalence
higher than 1%. By calculations of the mutation frequency per
replicative viral cycle (10⫺5 per site) and the exponential replication in a new host (29), a subpopulation of viruses with substantially superior fitness would already be noticeable when the replication plateau was reached, after 2 days. This time perspective is
April 2015 Volume 81 Number 7
FIG 2 Inhibition of early and late samples of the mutated A/51833/H274Y
virus and of the original A/51833/wt virus by OC and ZA. Results for early
(generations 1 and 2) and late (generation 10) samples are shown as mean IC50
for 8 duplicate samples. The IC50 for the original virus are means from 6
repeated assays. Boxes indicate the 95% CIs of the means, and whiskers indicate minimum and maximum values.
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Samplesa
g 1:1
g 2:1
g 2:2
g 10:1
g 10:2
g 10:1
No. of reads at bp
820 of the NA gene
supported by results from a previous study in this mallard model
where the resistant A/51833/H274Y virus emerged rapidly and
dominated over the A/51833/wt virus at a high drug pressure (23).
The possibility that minimally decreased fitness of the mutant
would go unnoticed under our experimental conditions cannot be
excluded, but we argue that substantial evolutionary space for
reversion was provided. We could not observe any wild-type virus
in 10 individuals after 17 days of successive propagation at OC
concentrations below the resistance-inducing level (including 14
days and 8 individuals at ⬍10% of the resistance-inducing level),
or in 4 individuals after 5 days without OC. Furthermore, the
NA-H274Y mutation was retained in all fecal samples through the
OC-free propagation process in embryonated chicken eggs, prior
to phenotypic testing.
Phenotypic testing confirmed the picture of retained resistance
in the A/51833/H274Y virus, with 340-fold lower sensitivity to OC
than the A/51833/wt virus, and with no significant difference between early and late samples. This level of OC sensitivity is the
same as that observed previously for this mutant (23). Infectivity
or transmissibility between mallards, evaluated by fecal shedding
of IAV, was not reduced when drug pressure was removed (Fig. 1),
and the level of IAV shedding was not lower than that of the
original A/51833/wt virus in previous studies (30). Based on the
retention of infectivity and transmissibility between mallards, and
on the persistence of the resistance mutation without drug pressure, we conclude that viral fitness was not significantly impaired
in this NA-H274Y resistant avian influenza A (H1N1) virus.
Permissive or compensatory mutations in an IAV are clearly
important for the ability of a virus to harbor a selected resistance
mutation (15, 31, 32). Several amino acid variants at NA position
222 can have both permissive and additive effects with NA-H274Y
in human influenza A (H1N1) virus (31, 33, 34), and it is possible
that the NA-N222 variant in this avian influenza A (H1N1) virus
might have had a permissive function for the acquisition and retention of NA-H274Y.
The highest OC concentrations detected in the environment to
date (0.86 ␮g/liter [18]) are lower than the lowest resistance-inducing concentration in the mallard model (0.95 ␮g/liter [23])
but in the same order of magnitude. Furthermore, occasional peak
concentrations may exceed detected levels, especially during pandemics, and different IAVs acquire resistance mutations at differ-
Gillman et al.
ACKNOWLEDGMENTS
We acknowledge the Swedish Research Council Formas, the Swedish Research Council (Vetenskapsrådet), and the Family Olinder-Nielsen’s
Foundation for financial support. We also acknowledge the National
Genomics Infrastructure (NGI)/Uppsala Genome Center and UPPMAX
for providing assistance in massive parallel sequencing and computational infrastructure. Work performed at the NGI/Uppsala Genome Center has been funded by RFI/VR and Science for Life Laboratory, Sweden.
Susanne Bloemberg and the rest of the staff at the animal facility of the
National Veterinary Institute, Uppsala, Sweden, are gratefully acknowledged for excellent animal care. F. Hoffman-La Roche Ltd. is acknowledged for providing OC, including the deuterium-labeled isotope.
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